Polymer NEMs for cell physiology and microfabricated cell positioning system for micro-biocalorimeter

ABSTRACT

A microfluidic embedded nanoelectromechanical system (NEMs) force sensor provides an electrical readout. The force sensor contains a deformable member that is integrated with a strain sensor. The strain sensor converts a deformation of the deformable member into an electrical signal. A microfluidic channel encapsulates the force sensor, controls a fluidic environment around the force sensor, and improves the read out. In addition, a microfluidic embedded vacuum insulated biocalorimeter is provided. A calorimeter chamber contains a parylene membrane. Both sides of the chamber are under vacuum during measurement of a sample. A microfluidic cannel (built from parylene) is used to deliver a sample to the chamber. A thermopile, used as a thermometer is located between two layers of parylene.

CROSS-REFERENCE TO RELATED APPLICATIONS

This application is a divisional application of the following UnitedStates patent application, which is incorporated by reference herein:

-   U.S. patent application Ser. No. 11/830,612, filed on Jul. 30, 2007,    for “POLYMER NEMS FOR CELL PHYSIOLOGY AND MICROFABRICATED CELL    POSITIONING SYSTEM FOR MICRO-BIOCALORIMETER” by MICHAEL L. ROUKES,    CHUNG WAH FON, WONHEE LEE, HONGXING TANG, BLAKE WATERS AXELROD, and    JOHN LIANG TAN, which application claims the benefit under 35 U.S.C.    Section 119(e) of the following commonly-assigned U.S. provisional    patent application(s), which is/are incorporated by reference    herein:-   Provisional Application Ser. No. 60/834,253, filed on Jul. 28, 2006,    by Michael L. Roukes, Chung-Wah Fon, Wonhee Lee, and Hongxing Tang,    entitled “Vacuum-insulating polymer-based micro-biocalorimeter    integrated with microfluidics”;-   Provisional Application Ser. No. 60/834,052, filed on Jul. 28, 2006,    by Blake W. Axelrod, Michael L. Roukes, and John Tan, entitled    “Plastic NEMs for cell physiology”; and-   Provisional Application Ser. No. 60/834,288, filed on Jul. 28, 2006,    by Blake W. Axelrod, Michael L. Roukes, and John Tan, entitled    “Microfabricated cell positioning system”;

STATEMENT REGARDING FEDERALLY SPONSORED RESEARCH AND DEVELOPMENT

The invention was made with Government support under Grant No.N66001-02-1-8914 awarded by NAVY-SPAWAR Systems Center San Diego, andGrant No. W911NF-04-1-0171 awarded by ARO—US Army Robert MorrisAcquisition Center. The Government has certain rights in this invention.

BACKGROUND OF THE INVENTION

1. Field of the Invention

The present invention relates generally to nanoscale electromechanical(NEMs) devices, and in particular, to a method, apparatus, and devicefor a micro-fluidic embedded polymer NEMs force sensor and vacuuminsulated polymer based micro-biocalorimeter integrated withmicrofluidics.

2. Description of the Related Art

(Note: This application references a number of different publications asindicated throughout the specification by reference numbers enclosed inbrackets, e.g., [x]. A list of these different publications orderedaccording to these reference numbers can be found below in the sectionentitled “References.” Each of these publications is incorporated byreference herein.)

The development of microcantilever force sensors has enabled developmentin the field of atomic force microscopy (AFM). AFMs are important toolsin nanoscience and have further led to the development of cantileverbased sensing, including a wide range of scanning probe microscopies(SPM), and many different forms of static (that is non-scanned) sensing.SPMs are used to image local forces arising from magnetic and magneticresonance interactions; forces from local electrostatics, surfacepotentials, surface temperatures, and chemical bonding; and forces frommany other local origins. Similarly, applications for non-scannedmicrocantilever sensors are equally diverse, including infrared imaging,nanocalorimetry, vapor- and liquid-phase chemisensing, electrometry,mass detection, etc.

However, at microscale dimensions, there are limits with respect to thelevel of frequency achievable and the level of sensitivity attainable.In this regard, the standard approaches used to makemicroelectromechanical systems (MEMS) cannot provide access to thenanoscale, where very large improvements in sensitivity can be attained[1]. Recent demonstrations and applications of the unprecedentedsensitivity available from nanoelectromechanical (NEMS) devices includemilestones such as sub-single-charge electrometry[2],single-electron-spin paramagnetic resonance [3], zeptogram-scale masssensing [4], zeptonewton-scale force sensing [5] and subfemtometerdisplacement sensing [6]. In fact, with these continuing advances, NEMSsensors are rapidly converging towards the ultimate, quantum limits offorce and displacement detection [7].

However, in contrast to MEMS, NEMS devices are still largely pursuedonly within the province of specialists. A current barrier to theirpractical development and widespread use is the difficulty of achievingsensitive displacement transduction at the nanoscale. Beyond the initialchallenges of fabricating ultra-small mechanical devices, successfulrealization of NEMS involves addressing the doubly hard challenge ofrealizing very high frequency displacement sensing while attainingextreme subnanometer resolution. This is not straightforward; approachesto displacement transduction commonly used for MEMS generally are notapplicable to NEMS [8]. For example, the efficiency of capacitivedetection precipitously decreases at the nanoscale, and the signal istypically overwhelmed by uncontrollable parasitic effects.

Existing prior art techniques used to measure forces exerted bybiological structures have been primarily limited to opticalmeasurements. For optical readouts, diffraction effects becomepronounced when device dimensions are scaled far below the wavelength ofthe illumination used. Furthermore, existing readouts for scanned probemicroscopy cantilevers are predominantly based upon external (that is,off-chip) displacement sensing systems that, typically, greatly exceedthe size scale of the cantilever sensors themselves. The most common SPMreadouts are optically based, involving simple optical beam deflectionor more sensitive interferometry. By comparison, only a relatively smallsubset of efforts has focused upon development of self-sensingnanocantilevers.

In addition to the above, the ability to measure forces exerted bybiological specimens have encountered significant limitations. In thisregard, prior art techniques have focused on optical measurementtechniques. In such an environment, the amount of resolution attainableis limited. Further, prior art techniques fail to provide an efficientmechanism to deliver individual cells to specific force sensors and failto precisely control the chemical environment around a cell under study.In addition, prior art delivery and control systems fail to maintain theviability of the biological sample under study while providing amechanism to extract signals from a force sensor to a computer forreadout and analysis.

In view of the above, what is needed is a NEMs force sensor for use inbiological applications that can be used in an efficient and controlledenvironment.

In addition to the above, calorimeters are used in the prior art todetect enthalpy change of chemical and biological reactions. However,measurement sensitivity of microfabricated calorimeters/thermometersfail to achieve the measurement sensitivity compatible to that of largescale calorimeters. Such a lack of measurement sensitivity is determinedby the sensitivity of the thermometer and capability to maximize thesignal with good thermal isolation. However, the prior art has failed toincrease sensitivity to minimize the heat loss of the sample.Accordingly, what is needed is a microcalorimeter that is useful inbiological applications and that provides sufficient measurementsensitivity.

SUMMARY OF THE INVENTION

One or more embodiments of the invention encompasses a force sensingnanoscale electromechanical (NEMs) device for biological applications,such as the contraction of a cell's lamellipodia. The force sensor is adoubly clamped beam fabricated from a polymer, such as SU-8, with apiezoresistive strain sensor patterned asymmetrically through the beamso as to integrate over the regions of maximum tensile strain. Thepiezoresistive strain sensor is made from a conductor, such as a metallike gold. The force sensor can be positioned next to a ledge orsuspended bridge for supporting a single cell and performing forcemeasurements on cell contraction. If the entire device is mounted on aflexible substrate the force-sensing beam can also be used to exertforce back on a cell by flexing the substrate parallel to the beam.Furthermore, the stiffness of the force sensor can be tuned by flexingthe substrate perpendicular to the beam.

In addition, one or more embodiments of the invention providecalorimeter capable of detection of enthalpy change of chemical andbiological reaction, such as enzyme activity and protein-ligand binding,in a 3.5 nanoliter (nL) volume. The calorimeter is embedded in parylenemicrofluidic system and can be coupled to other lab-on-a-chipmicrofluidic devices. Microfabrication of the calorimeter array and theaccompanying microfluidic circuitry has enabled rapid and parallelimplementation of calorimetric measurement. The reduction in scale alsoreduces the time and sample quantity required for such measurement.Sophisticated thermal insulation is engineered to maximize themeasurement sensitivity. While a batch calorimeter is demonstrated, thecalorimeter can be modified to perform isothermal titration,differential scanning and flow calorimetry.

BRIEF DESCRIPTION OF THE DRAWINGS

Referring now to the drawings in which like reference numbers representcorresponding parts throughout:

FIG. 1 illustrates a c-shape strain sensor used in accordance with oneor more embodiments of the invention;

FIG. 2 illustrates a straight-line strain sensor in accordance with oneor more embodiments of the invention;

FIG. 3 illustrates the various dimensions of a beam and strain sensorused in accordance with one or more embodiments of the invention;

FIG. 4A illustrates the estimated force resolution for SU-8 beams inaccordance with one or more embodiments of the invention;

FIG. 4B compares SU-8 and silicon beams in accordance with one or moreembodiments of the invention;

FIG. 5 illustrates a polymer strain sensor fabricated in accordance withone or more embodiments of the invention;

FIG. 6A shows the response of the beam to a stepwise increase anddecrease in applied force in accordance with one or more embodiments ofthe invention;

FIG. 6B shows the force sensitivity as a function of time resolution fora beam in accordance with one or more embodiments of the invention;

FIG. 7 illustrates how the distance between the beam and the ledge canbe increased by bending the substrate in accordance with one or moreembodiments of the invention;

FIG. 8 illustrates a derivation of an equation for the radius ofcurvature in accordance with one or more embodiments of the invention;

FIG. 9 shows the maximum beam displacement as a function of the beam toledge separation, which must be kept small enough to allow a cell'slamelipodia to span the gap in accordance with one or more embodimentsof the invention;

FIG. 10A illustrates a force application with a glass substrate and FIG.10B illustrates a force application with a plastic substrate inaccordance with one or more embodiments of the invention;

FIG. 11 illustrates the tuning of a spring constant in accordance withone or more embodiments of the invention;

FIG. 12 illustrates an image of a force sensor in accordance with one ormore embodiments of the invention;

FIG. 13 illustrates a polymer NEMs force sensor embedded inmicrofluidics in accordance with one or more embodiments of theinvention;

FIG. 14 illustrates a 2D diagram of the four layers that make up themicrofluidics in accordance with one or more embodiments of theinvention;

FIG. 15 illustrates a system used to position NIH 3T3 fibroblast cellson plastic NEMs devices in accordance with one or more embodiments ofthe invention;

FIG. 16 shows a SEM image of a dry force sensor prior to micro-fluidicencapsulation and a fluorescent image of a cell attached to the forcesensor on a micro-fluidics encapsulated device in accordance with one ormore embodiments of the invention;

FIG. 17 shows force vs. time data from a single cell showing a stableforce in growth media, collapse of that force when the cytoskeletondisrupting agent Cytochalasin D is introduced, and the recovery of theforce when the Cytochalasin D is removed in accordance with one or moreembodiments of the invention;

FIG. 18 illustrates a cross section of such a multilayer parylenecalorimeter compartment in accordance with one or more embodiments ofthe invention;

FIG. 19 shows the reaction chamber on a suspended parylene membrane, themicrofluidics channels for fluid delivery, and the thermopile forsensing heat release in accordance with one or more embodiments of theinvention;

FIG. 20 illustrates a schematic of a calorimeter in accordance with oneor more embodiments of the invention;

FIG. 21 illustrates a whole chip embodying the calorimeter in accordancewith one or more embodiments of the invention;

FIG. 22 illustrates a detailed view of a calorimeter chamber andelectric sensor built on a parylene membrane in accordance with one ormore embodiments of the invention;

FIG. 23 is an image illustrating an alignment of the fluidic channels onparylene channels in accordance with one or more embodiments of theinvention;

FIG. 24 illustrates three images of merging two reactants in accordancewith one or more embodiments of the invention;

FIG. 25 shows the effect of a vacuum on device thermal conductance inaccordance with one or more embodiments of the invention;

FIG. 26 illustrates the logical flow for creating and utilizing amicrofluidic embedded NEMS force sensor in accordance with one or moreembodiments of the invention; and

FIG. 27 illustrates a method for utilizing a microfluidic embeddedvacuum insulated biocalorimeter in accordance with one or moreembodiments of the invention.

DETAILED DESCRIPTION OF THE PREFERRED EMBODIMENTS

In the following description, reference is made to the accompanyingdrawings which form a part hereof, and which is shown, by way ofillustration, several embodiments of the present invention. It isunderstood that other embodiments may be utilized and structural changesmay be made without departing from the scope of the present invention.

Overview—Microfluidic Embedded Polymer NEMs Force Sensor

As described above, prior art techniques have attempted to measure theforces exerted by biological samples (e.g., single cells). In thisregard, adherence cells (i.e., cells that adhere or have adheringproperties with respect to adjacent surfaces), may exert forces whendiffused across a surface. Prior art mechanisms attempted to measuresuch forces primarily utilizing optical means. In this regard, prior artmechanisms were based on optical measurements of deflected substrates ormembers. For example, cells (e.g., monocyte or macrophage cells), may beplaced superior to polydimethylsiloxane (PDMS) (e.g., PDMSpillars/structures) and any resulting deformation in the PDMS structurewas optically measured. However, the resolution of such measurements wasinsufficient. In this regard, prior art mechanisms were insufficient formeasuring the displacement/deformation of single cell structures.Further, such optical measurement techniques are expensive and celldelivery and control is difficult.

To overcome the disadvantages of the prior art, one or more embodimentsof the invention utilize a microfluidic embedded polymer NEMs forcesensor. To more easily understand the invention, a description of theoverview of the force sensor and microfluidics are followed withindependent descriptions of the force sensor and the microfluidicaspects of the invention.

One or more embodiments of the invention provide a force sensor forbiological applications, e.g. measuring forces exerted by a single cell.The force sensor may consist of a doubly clamped beam fabricated from apolymer (e.g., plastic) with a piezo resistive strain sensor patternedasymmetrically through the beam so as to couple to regions of maximumtensile or compressive strain. Beams can be fabricated using thefollowing polymers: SU Polymer family (e.g., SU8 2000, SU-8 3000, etc.)PolyImide, Parylene. The piezo resistive strain sensor can be made fromany conductive material (e.g., a metal such as gold with a very thintitanium or chromium adhesion layer).

Beams can been fabricated for measuring in-plane forces by patterningthe piezo-resistive strain sensor 102 asymmetrically in the horizontalplane using a c-shape and symmetrically out of the plane by sandwichingthe strain sensor 102 between two layers of polymer (e.g., plastic) ofthe same thickness. FIG. 1 illustrates a c-shape strain sensor 102 inaccordance with one or more embodiments of the invention. Asillustrated, the piezo-resistive strain sensor 102 is patternedasymmetrically in the horizontal plane of the beam. The pattern is basedon those areas of the beam that are likely to stretch or strain as aresult biological force exertion. The biological sample 104 is placedwith respect to a defined location 106 of the beam 108 and the strain ofthe piezo-resistive strain sensor 102 is able to measure the in-planeforces/displacement (indicated by arrow 110) of the beam caused by theintroduction of the biological sample 104.

Beams have also been fabricated for measuring to out-of-plane forces bypatterning the piezo-resistive strain sensor 102 symmetrically in thehorizontal plane using a straight line pattern and asymmetrically out ofthe plane by placing the strain sensor 102 on top of or on the bottom ofthe polymer/plastic layers or by sandwiching the strain sensor 102between two layers of polymer/plastic of different thickness. FIG. 2illustrates a straight-line strain sensor in accordance with one or moreembodiments of the invention. As illustrated in FIG. 2, the strainsensor 102 is fabricated in a straight-line pattern to measureout-of-plane forces indicated by arrow 202.

For applications in fluid, particularly buffered solutions used inbiological applications, it is advantageous to sandwich the strainsensor 102 between two layers of polymer (e.g., plastic) in order toelectrically isolate the strain sensor 102 from the fluid. Suchisolation insulates the force/strain sensor 102 and isolates the sensor102 from any conductivity present in the buffered solution/fluid.

The force sensors can be encapsulated in PDMS (poly-dimethylsiloxane)microfluidics for use in fluid. Multi-layer microfluidics with controlvalves may be mounted on the front side of the chip with the forcesensor. A glass cover slip can also be mounted on the backside of thechip and sealed with a thin layer of PDMS. The glass cover slip enableshigh resolution microscopy simultaneously with use of the force sensor.

Polymer NEMs Force Sensor

Described below is a detailed description of the force sensor used inaccordance with embodiments of the invention.

Various symbols may be used in the description that follows. Thefollowing presents a list of such symbols and their intended meaning

α—material dependent hooge parameter

E—Young's modulus

ε—strain

F—force

f—frequency

ζ—thickness of piezoresistive wire

G—tension force

I—moment of intertia

K—spring constant

k_(B)—Boltzmann's constant

κ—transducer responsivity

l—substrate length

L—length of beam

λ—filter setting

N—number of carriers

n—carrier density

π₁—longitudinal piezoresistance coefficient

R—resistance

δR—change in resistance

r(x)—radius of curvature

{right arrow over (r)}—cartesian vector

{right arrow over (ρ)}—cartesian vector

ρ—resistivity

S_(Th)—thermal noise voltage spectral density

S_(H)—hooge noise voltage spectral density

σ₀—surface stress distribution

T—substrate thickness

t—thickness of beam

τ—time constant

V₀—input voltage

δV—voltage signal

υ—poison ratio, width of piezoresistive wire

w—width of beam

x—x-coordinate

y—y-coordinate

ΔX(r)—displacement of surface at r in x direction

ΔY(x)—displacement of centerline of beam in y direction

δz—vertical displacement

I. Device: Clamped Beam with Piezoresistive Strain Gauge

a. Beam Displacement and Spring Constant

The displacement of the center line of a doubly clamped beam due to aforce exerted at the beam's mid point is given by:

$\begin{matrix}{{{\Delta\;{Y(x)}} = {F\frac{x^{2}\left( {{3L} - {4x}} \right)}{4E\; t\; w^{3}}}},} & (1)\end{matrix}$where x extends from zero to L/2, t, w, and L are the thickness, widthand length of the beam as shown in FIG. 3, E is the young's modulus andF is the applied force [P1]. Accordingly, FIG. 3 illustrates the variousdimensions of a beam and strain sensor used in accordance with one ormore embodiments of the invention.

The effective spring constant, K, is defined by the displacement at themidpoint, x=L/2:

$\begin{matrix}{K = {\frac{F}{\Delta\;{Y\left( {x = {L/2}} \right)}} = {\frac{16E\; t\; w^{3}}{L^{3}}.}}} & (2)\end{matrix}$Equation (2) has been checked with CFDRC and agrees within half of onepercent. Table 1 (below) lists in plane (ky) and out of plane (kz)spring constants for a few relevant geometries and material properties.Two things of note, first the smallest silicon beams are roughly afactor of 30 stiffer than the smallest Su8 beams, second the Su8 beamsare roughly a factor of 50 stiffer than the gold beams which can bepatterned inside of them.

b. Strain in Piezoresistor

A strain gauge is integrated into the beam by patterning a u-shapedpiezoresistive (PZR) conductor of width υ and thickness ζ symmetricallyacross the four quarters of the beam, shown FIG. 3. The u-shaped patternwill maximize the strain induced by the displacement described in eq(1). The strain in an infinitesimal element of the PZR conductor at x,yis given by [P1]:

$\begin{matrix}{{ɛ = \frac{y}{r(x)}},} & (3)\end{matrix}$where y is the displacement in the ŷ direction from the center line ofthe beam and r is the radius of curvature of the center line at thatpoint. One can approximate the radius of curvature:

$\begin{matrix}{\frac{1}{r(x)} = {{\frac{\mathbb{d}^{2}}{\mathbb{d}x^{2}}\Delta\;{Y(x)}} = {F{\frac{{6L} - {24x}}{4E\; t\; w^{3}}.}}}} & (4)\end{matrix}$Each quarter of the piezoresistor will be symmetric with strain, thusone need only integrate over one quarter of the wire to determine theaverage strain:

$\begin{matrix}{{\overset{\_}{ɛ} = {{\frac{1}{area}{\int{\frac{y}{r(x)}{\mathbb{d}({area})}}}} = {\frac{F}{(\upsilon)\left( {L/4} \right)}{\int_{{w/2} - \upsilon}^{w/2}{\int_{0}^{L/4}{\frac{y\left( {{6L} - {24x}} \right)}{4E\; t\; w^{3}}{\mathbb{d}x}{\mathbb{d}y}}}}}}},} & (5)\end{matrix}$which is easily integrated:

$\begin{matrix}{\overset{\_}{ɛ} = {\frac{3}{8}\frac{F}{E}{\frac{L\left( {w - \upsilon} \right)}{t\; w^{3}}.}}} & (6)\end{matrix}$Equation (6) has also been checked with CFDRC and agrees within 1%.

c. Wheatstone Bridge and Transducer Responsivity

The strain gauge will use the piezoresistance effect to convert theinduced strain, eq (6), into a change in resistance:

$\begin{matrix}{{\frac{\delta\; R}{R} = {{\pi_{l}\overset{\_}{ɛ}} = {\frac{3}{8}\frac{\pi_{l}}{E}\frac{L\left( {w - \upsilon} \right)}{t\; w^{3}}F}}},} & (7)\end{matrix}$where π_(l) is the piezoresistance coefficient for the wire. For thesilicon in the BioNEMs chips, one expects a π_(l) of 40 and roughly 47have been measured for the transducer responsivity with the AFM. Forgold, geometric considerations predict a π_(l) of 2 for bulk metals, butThaysen et. al. [P2] report a value of roughly 4; the discrepancy ispossibly due to thin film effects.

The force sensing beam may be integrated into an on chip Wheatstonebridge with one suspended reference beam and two supported balanceresistors. When optimally balanced the Wheatstone bridge converts achange in resistance into a voltage signal according to:

$\begin{matrix}{{{\delta\; V} = {V_{0}\frac{1}{4}\frac{\delta\; R}{R}}},} & (8)\end{matrix}$where V₀ is the voltage applied to the bridge. Combining equations (7)and (8) one obtains the proportionality constant between the appliedforce and the measured voltage signal—the transducer responsivity, κ, ofthe force sensing beam:

$\begin{matrix}{{{\delta\; V} = {{\frac{3}{32}\frac{\pi_{l}}{E}\frac{L\left( {w - \upsilon} \right)}{t\; w^{3}}V_{0}F} = {\kappa\; F}}},} & (9) \\{\kappa = {\frac{3}{32}\frac{\pi_{l}}{E}\frac{L\left( {w - \upsilon} \right)}{t\; w^{3}}V_{0}}} & (10)\end{matrix}$

d. Electrical Noise

There will be four electrical contributions to the noise: amplifiervoltage noise e_(n), amplifier current noise i_(n), Johnson noise, and1/f noise. The voltage spectral density of Johnson noise is frequencyindependent:

$\begin{matrix}{{S_{T\; h} = {{4k_{B}T\; R} = \frac{4k_{B}T\;\rho\; L}{\zeta\upsilon}}},} & (11)\end{matrix}$where the second equality comes from the geometric dependence of theresistance. The amplifier voltage and current noise spectral densities,e_(n) ² and i_(n) ², are also frequency independent. Hooge noise, or1/f-noise, is named after its' frequency dependence:

$\begin{matrix}{{S_{H} = {\frac{\alpha\; V^{2}}{fN} = \frac{\alpha\; V^{2}}{{fn}\;\zeta\;{vL}}}},} & (12)\end{matrix}$where α is material dependent, N is the number of carriers and n is thedensity of carriers. The noise voltage power is determined byintegrating the spectral density over the measurement frequency range:

$\begin{matrix}{\left\langle V_{Noise}^{2} \right\rangle = {{\left( {f_{\max} - f_{\min}} \right)\left( {\frac{4k_{B}T\;\rho\; L}{\zeta\; v} + e_{n}^{2} + \left( \frac{i_{n}\rho\; L}{2\zeta\; v} \right)^{2}} \right)} + {\frac{\alpha\; V^{2}}{n\;\zeta\;{vL}}{\ln\left\lbrack \frac{f_{\max}}{f_{\min}} \right\rbrack}}}} & (13)\end{matrix}$

The force noise is determined by combing equations (9) and (13):

$\begin{matrix}{F_{Noise}^{2} = {\left( {\frac{32}{3}\frac{E}{\pi_{l}}\frac{1}{V_{0}}\frac{{tw}^{3}}{L\left( {w - v} \right)}} \right)^{2}{\left( {{\left( {f_{\max} - f_{\min}} \right)\left( {\frac{4k_{B}T\;\rho\; L}{\zeta\; v} + e_{n}^{2} + \left( \frac{i_{n}\rho\; L}{2\zeta\; v} \right)^{2}} \right)} + {\frac{\alpha\; V^{2}}{n\;\zeta\;{vL}}{\ln\left\lbrack \frac{f_{\max}}{f_{\min}} \right\rbrack}}} \right).}}} & (14)\end{matrix}$

The bandwidth, f_(min), and f_(max), is determined by the lock-inamplifier used, in particular the source frequency f, the time constantΣ, and the low pass filter roll-off. For the following I assume a SRS830 lock-in with source frequency of 100 kHz, a minimum time-constant of10 μs and low pass filter settings of 6 db/oct, 12 db/oct, 18 db/oct or24 db/oct. The time resolution δ will be determined by the time constantand low pass filter settings, Table 2 summarizes the relationshipbetween these three variables.

TABLE 2 Equivalent noise bandwidth (f_(max) − f_(min)) Time resolution,δ ¼τ = 5/4δ = λδ 5τ ⅛τ = ⅞δ = λδ 7τ 3/32τ = 27/32δ = λδ 9τ 5/64τ =50/64δ = λδ 10τ 

For a given filter setting, λ, and source frequency, f, one candetermine the force noise and thus force resolution as a function of thetime resolution):

$\begin{matrix}{F_{Noise} = {\left( {\frac{32}{3}\frac{E}{\pi_{l}}\frac{1}{V_{0}}\frac{{tw}^{3}}{L\left( {w - v} \right)}} \right)*{\sqrt{\left( {{\frac{\lambda}{\delta}\left( {\frac{4k_{B}T\;\rho\; L}{\zeta\; v} + e_{n}^{2} + \left( \frac{i_{n}\rho\; L}{2\zeta\; v} \right)^{2}} \right)} + {\frac{\alpha\; V^{2}}{n\;\zeta\;{vL}}{\ln\left\lbrack \frac{f + {{\lambda/2}\delta}}{f - {{\lambda/2}\delta}} \right\rbrack}}} \right)}.}}} & (15)\end{matrix}$

One may apply the noise analysis embodied in eq. (15) and table (2) withthe appropriate optimized bandwidth and filter settings for an SRS 560pre-amp and SRS 830 lock-in amplifier to the 36 different combinationsof materials, beam dimensions and PZR strain gauge dimensions listed intable (3).

The principle piece missing from this analysis is an optimization of theinput voltage applied to the Wheatstone bridge. Fluidic noise, whichwill be discussed in the following section is also missing from thisanalysis, but is expected to be negligible. The estimated forceresolution for the Su8 beams is plotted in FIG. 4A, for the siliconbeams identified in the inset of FIG. 4A. FIG. 4B compares the Su8 andsilicon beams.

The results of this noise analysis indicate that beams #20 & 21, made ofSu8 with length 100 μm, width 1 μm, thickness 400 nm, PZR thickness 50nm and PZR widths 200 nm and 100 nm respectively, yield the best forceand time resolution: 120 pN at 10 μs, 20 pN at 100 μs and 6.5 pN at 1ms. The best silicon beams, by comparison, are #34 & 35 which offerforce resolution of 2 nN at 10 μs, 280 pN at 100 μs and 80 pN at 1 ms;roughly a factor of 15 worse than the best Su8 beams.

The dynamic range of this measurement can be determined by the onset ofnon-linearity within the beam.

e. Demonstration of Strain Sensor

Polymer (e.g., plastic) strain sensors (as described above) have beensuccessfully fabricated with a length of 100 microns, a width of 4microns, a thickness of 530 nm and with a gold piezoresistive straingauge that is 500 nm wide and 40 nm thick. FIG. 5 illustrates a polymerstrain sensor fabricated in accordance with one or more embodiments ofthe invention.

The device of FIG. 5 has been calibrated using a glass micro needle. Thetransducer responsivity is 65 V/N at a drive voltage of 0.5 Vrms. FIG.6A shows the response of the beam to a stepwise increase and decrease inapplied force. FIG. 6B shows the force sensitivity as a function of timeresolution for this beam.

f. Force Application by Device

The plastic, SU-8, beams may be attached to a flexible substrate andthen by bending the substrate it is possible to either change thedistance between the beam and the ledge or to apply a tension to thebeam, depending on whether the bending axis is parallel or perpendicularto the beam. FIG. 7 illustrates how the distance between the beam andthe ledge can be increased by bending the substrate in accordance withone or more embodiments of the invention. As illustrated, the topportion of FIG. 7 illustrates the beam without any bending of thesubstrate (and a distance of x). Once the substrate is bent, asillustrated in the bottom portion of FIG. 7, the distance between thebeam and the ledge increases (i.e., x+δx).

Application of equation (3) to the geometry in FIG. 7 gives thedisplacement, δx, in terms of the curvature of the substrate:

$\begin{matrix}{{\frac{\delta\; x}{x} = \frac{\left( {T/2} \right)}{r}},} & (23)\end{matrix}$where one may assume that the neutral plane of the deflection is in themiddle of the flexible substrate. If the radius of curvature issufficiently large, r>>1, then it can be expressed in terms of δz:

$\begin{matrix}{\frac{1}{r} = {\frac{6\delta\; z}{l^{2}}.}} & (24)\end{matrix}$

The derivation of equation (24) is shown in FIG. 8.

By combining equations (23) and (24) one obtains the displacement interms of the vertical displacement, δz, which is the relevantexperimental variable:

$\begin{matrix}{{\delta\; x} = {\frac{3{Tx}}{l^{2}}\delta\;{z.}}} & (25)\end{matrix}$

This result differs from a similar derivation by Ruitenbeek et. al.[P23] by a factor of 2 in which the neutral surface is assumed to be atthe bottom surface of the flexible substrate.

In the experimental setup described herein, the vertical displacementmay be controlled by a piezoelectric stage such as a long-travel piezoflexure stage (e.g., part number P-290 available from Physik Instrumente(PI) GmbH & Co. KG) which has a maximum travel of 1000 μm and anopen-loop displacement resolution of 20 nm. The displacement resolutionis limited by the voltage noise of the amplifier used to drive thepiezoelectric stage. Potential substrates include number 1 cover glass(T=250 μm) or stiff plastic (T=1000 μm)—cover glass will enable highresolution microscopy, whereas the plastic will enable greater forceapplication. A substrate width, l, of 2 cm is necessary to enableelectronic and fluidic integration/fanout. FIG. 9 shows the maximum beamdisplacement as a function of the beam to ledge separation, which mustbe kept small enough to allow a cells lamelipodia to span the gap.

The force exerted on the cell by displacing the beam as described abovewill depend on the spring constant of the beam, given by equation (2),and Hook's law:

$\begin{matrix}{F = {{K\;\delta\; x} = {\left( \frac{16{Etw}^{3}}{L^{3}} \right)\left( \frac{3{Tx}}{l^{2}} \right)\delta\;{zw}^{3}\mspace{14mu}\ldots}}} & (26)\end{matrix}$

FIGS. 10A and 10B show the force resolution and maximum force that canbe applied by the beams analyzed in section (d) above as a function ofbeam width for a cover glass substrate and a plastic substrate with abeam to ledge separation of 4 μm. In this regard, FIG. 10A illustrates aforce application with a glass substrate and FIG. 10B illustrates aforce application with a plastic substrate in accordance with one ormore embodiments of the invention.

g. Device Stiffening: Tuning the Spring Constant

The previous section detailed how bending of the substrate can be usedto move the beam with respect to the ledge and thus exert a force on thecell under study. The same principle can be used to apply a tension tothe beam that will increase the beam's effective spring constant bybending the substrate around an axis perpendicular to the beam.Replacing the beam to ledge distance, x, in equation (25) with thelength of the beam, L, one obtains an expression for the change inlength of the beam as a function of the vertical extension, δz:

$\begin{matrix}{{\delta\; L} = {\frac{3{TL}}{l^{2}}\delta\;{z.}}} & (27)\end{matrix}$

The tension induced from this extension of the beam is:

$\begin{matrix}{G = {{{Etw}\frac{\delta\; L}{L}} = {\frac{3{ETtw}}{l^{2}}\delta\;{z.}}}} & (28)\end{matrix}$

The displacement of the center line of a doubly clamped beam undertension force, G, due to a force, F, exerted at the beam's mid point isgiven by:

$\begin{matrix}{{{\Delta\;{Y(x)}} = {\frac{F}{2G}\left( {x - {\frac{1}{k}{{Sinh}({kx})}} + {\frac{{{Cosh}\left( \frac{kL}{2} \right)} - 1}{{kSinh}\left( \frac{kL}{2} \right)}\left( {{{Cosh}({kx})} - 1} \right)}} \right)}},{k = {\sqrt{\frac{G}{EI}} = {\sqrt{\frac{12G}{{Etw}^{3}}} = {\frac{6\sqrt{T\;\delta\; z}}{wl}.}}}}} & (29)\end{matrix}$

Similar to the analysis in section (a) of the beam without tension, onecan define the effective spring constant, K, by the displacement at themidpoint, x=L/2:

$\begin{matrix}\begin{matrix}{K = \frac{F}{\Delta\;{Y\left( {x = {L/2}} \right)}}} \\{= {\frac{36{{Etw}\left( {T\;\delta\; z} \right)}^{3/2}}{\begin{matrix}{{3{Ll}^{2}\sqrt{T\;\delta\; z}} - {\left( {wl}^{3} \right){Sinh}\left( \frac{3L\sqrt{T\;\delta\; x}}{wL} \right)} +} \\{\left( {wl}^{3} \right)\frac{\left( {{{Cosh}\left( \frac{3L\sqrt{T\;\delta\; z}}{wL} \right)} - 1} \right)^{2}}{{Sinh}\left( \frac{3L\sqrt{T\;\delta\; z}}{wL} \right)}}\end{matrix}}.}}\end{matrix} & (30)\end{matrix}$

Equation (30) may be simplified with the observation that wl³<<3 Ll²√(Tδz):

$\begin{matrix}{K = \frac{12{EtwT}\;\delta\; z}{{Ll}^{2}}} & (31)\end{matrix}$which, is clearly not correct because the spring constant in equation(31) goes to zero when the vertical displacement goes to zero, but thespring constant should revert to equation (2). If one views the above asa calculation of the change in spring constant due to the verticaldisplacement, then, the total spring constant would be the sum ofequations (2) and (31):

$\begin{matrix}{{K = {{\frac{16{Etw}^{3}}{L^{3}} + \frac{12{EtwT}\;\delta\; z}{{Ll}^{2}}} = {\frac{4{Etw}}{L}\left( {\frac{4w^{2}}{L^{2}} + \frac{3T\;\delta\; z}{l^{2}}} \right)}}},} & (31)\end{matrix}$A plot of the spring constant as a function of the vertical displacementfor the beams discussed in section (d) and the substrates discussed insection (f) is shown in FIG. 11. Accordingly, FIG. 11 shows that thechange in spring constant for the wide beams (4 μm) is negligible, butfor the thin beams (1 μm) the spring constant increases by a factor of 5on the glass substrate and 20 on the plastic.

II. Device Fabrication

Prior art techniques describe optically patterning SU-8 cantilevers andmetal wires to use as piezo-resistive strain sensors (e.g., deformablemembers), made from polymers, with transducers for convertingdeformation into an electrical signal. Additionally, the prior artdescribes a sacrificial chrome release layer and SU-8 plastic chip thatwere used in early versions of plastic NEMS, but not in more recentversions (see Thaysen [P2]). However, the prior art cantilevers areintended for use in Atomic Force Microscopes (AFM) and are not embeddedin microfluidics. In addition, the prior art utilizes a polymer layer asa “handle” or substrate.

In view of the above, prior art techniques for force measurements wereprimarily obtained based on optical measurements of deflected substratesor members. Further, prior art techniques do not utilize microfluidics.For example, some prior art techniques utilize soft substrates embeddedwith fluorescent beads, optical detection of deformation of substrate bycell, an optical readout, heavy computation requirements to extractprobabilistic force maps, limited force resolution due to opticalreadout, limited time resolution due to optical readout & substratestiffness, and very limited throughput due to computation requirements(see Lo [P18]).

Further, Tan [P19] describes soft posts marked with fluorescent dye,optical detection of deformation of posts by cell, optical readout,limited force resolution due to optical readout, and limited timeresolution due to optical readout & substrate stiffness.

One or more embodiments of the present invention overcome thedisadvantages of the prior art. In this regard, embodiments of thepresent invention utilize electrical detection of the deformation,electrical readout, and micro-fluidics. Further, embodiments may utilizestand alone chips as force sensors, may embed force sensors in themicro-fluidics and utilize the force sensors for/in biologicalapplications. In addition, while early designs of the invention may haveused an all polymer method, embodiments of the present invention maybuild polymer force sensors on top of a silicon wafer with openingsthrough the wafer to suspend the force sensors. Also, MPTS adhesionpromoters may be utilized. Further, embodiments may use a hot, dilutehydrofluoric acid to selectively etch silicon-nitride in the presence ofthe polymer force sensors. Such differences between embodiments of thepresent invention and the prior art may be better understood with adetailed explanation of the fabrication techniques that may be utilized.

The force sensors can be fabricated using an all SU-8 process thatproduces a finished chip which is all plastic and thus flexible. Thefabrication steps for this process are as follows:

1. Deposition of a sacrificial chrome layer onto a silicon wafer.Typically a Ti/Au layer is included below the chrome to aid in theremoval of the chrome.

2. Deposition of the first polymer layer for the force sensor. Thepolymer can be any polymer in the SU-8 polymer family (e.g., SU-8 2000or SU-8 3000). The polymer layer can be patterned using a direct writeof ebeam lithography or photolithography—typically a combination of bothis used. Or the layer can remain unpatterned until later—see step 6.

3. Deposition of the metal wire that makes up the piezo-resistiveelement of the strain sensor. The wire is patterned in PMMA (polymethylmethacrylate) using electron-beam lithography and deposited usingelectron-beam or thermal evaporation and lift-off in solvent—acetone,tricholorethylene. Typically gold is used as the metal with a thintitanium or chromium adhesion layer. A spin-on organic titanate (AP300)is used to aid adhesion to the polymer layer.

4. Deposition of the second polymer layer for the force sensor. SU-82000 or SU-8 3000. The polymer layer can be patterned using a directwrite of ebeam lithography or photolithography—typically a combinationof both is used. Or the layer can remain unpatterned.

5. Optional patterning and deposition of a metal layer for controllingcell adhesion to the force sensor by creating differences inhydrophobicity between this metal layer and the surrounding polymer orby utilizing surface chemistry differences between the metal layer andsurrounding polymer. Patterned in PMMA using electron-beam lithographyand deposited using electron-beam or thermal evaporation and lift-off insolvent—acetone, tricholorethylene. Typically gold is used as the metalwith a thin titanium or chromium adhesion layer. A spin-on organictitanate (AP300) is used to aid adhesion to the polymer layer.

6. Optional patterning of the polymer layers if they were not directlypatterned using lithography in steps 2 & 4. The polymer layers arepatterned using an oxygen based plasma etch with a mask to protect theregions which are to remain as structural elements on the force sensor.Typically a metal such as chrome or titanium is used as the etch maskand patterned using electron-beam lithography in PMMA. Electron-beamsensitive polymers such as PMMA and UVN-30 have also been used as etchmasks.

7. Patterning and deposition of metal layer for fan-out. A thick metallayer, typically gold with a thin titanium or chrome adhesion layer, ispatterned using a bi-layer resist, photolithography and lift-off.Typically 500-1000 nm of metal is necessary to protect wires frombreaking when chip flexes.

8. Deposition and patterning of thick polymer layer that will make upthe structural support layer of the final chip. Typically 60-80 micronsthick SU-8 2000 or SU-8 3000. Vias are patterned with photolithographyso that the force sensors will be suspended over openings in the thickpolymer layer. It is important that this layer have very low internalstress, low baking temperatures and long baking times are used toachieve low stress.

9. Release of the polymer chip from the silicon wafer by wet etching thesacrificial chrome layer. Best results are achieved by drying thereleased chips using a critical point drier.

The force sensors can also be fabricated using a silicon-nitride coatedsilicon wafer as a substrate. This process results in a rigid finishedchip, but gives much higher yields. The fabrication steps for thisprocess are as follows:

1. Optional patterning and deposition of a metal layer for controllingcell adhesion to the force sensor by creating differences inhydrophobicity between this metal layer and the surrounding polymer orby utilizing surface chemistry differences between the metal layer andsurrounding polymer. Patterned in PMMA using electron-beam lithographyand deposited using electron-beam or thermal evaporation and lift-off insolvent—acetone, tricholorethylene. Gold is used as the metal with anorganic mercapto-silane monolayer as an adhesion layer. The organicadhesion layer is deposited from an aqueous solution after developingthe PMMA and prior to evaporating the metal

2. Deposition of the first polymer layer for the force sensor. SU-82000, SU-8 3000, Poly-Imide or parylene can be used. Typically the layeris left unpatterned. However, the SU-8 resists can be directly patternedusing electron-beam or photo lithography at this stage.

3. Deposition of the metal wire that makes up the piezo-resistiveelement of the strain sensor. The wire is patterned in PMMA usingelectron-beam lithography and deposited using electron-beam or thermalevaporation and lift-off in solvent—acetone, tricholorethylene.Typically gold is used as the metal with a thin titanium or chromiumadhesion layer. A spin-on organic titanate (AP300) is used to aidadhesion to the polymer layer.

4. Deposition of the second polymer layer for the force sensor. SU-82000, SU-8 3000, Poly-Imide or parylene can be used. Typically the layeris left unpatterned. However, the SU-8 resists can be directly patternedusing electron-beam or photo lithography at this stage.

5. Optional patterning of the polymer layers if they were not directlypatterned using lithography in steps 2 & 4. The polymer layers arepatterned using an oxygen based plasma etch with a mask to protect theregions which are to remain as structural elements on the force sensor.Typically a metal such as chrome or titanium is used as the etch maskand patterned using electron-beam lithography in PMMA. Electron-beamsensitive polymers such as PMMA and UVN-30 have also been used as etchmasks.

6. Patterning and deposition of metal layer for fan-out. A thick metallayer, typically gold with a thin titanium or chrome adhesion layer, ispatterned using a bi-layer resist, photolithography and lift-off.Typically 200-300 nm of metal is used.

7. Through wafer silicon etch to open vias below the device regions. Thebackside of the wafer is patterned using photolithography and a windowis opened in the silicon-nitride layer using a fluorine based plasmaetch. A hot KOH etch is used to etch holes through the silicon waferleaving only silicon nitride membranes beneath the plastic forcesensors.

9. The plastic force sensors are released by preferentially etching thesilicon-nitride membrane without damaging the plastic beams. A fluorinebased plasma is used to thin the membrane from the back side of thewafer. The membrane removal is finished using a hot, dilute hydrofluoricacid bath which etches silicon nitride without damaging the plastic andmetal that comprise the force sensor. After the silicon-nitride membranehas been removed the devices are dried using a critical point drier.

In view of the above described fabrication techniques, FIG. 12illustrates an image of a force sensor in accordance with one or moreembodiments of the invention. The image is a Scanning ElectronMicroscope (SEM) image of two force sensors adjacent to a single cellcontact area before encapsulation in micro-fluidics. Each force sensorconsists of a deformable member and a transducer for reading out themember's deformation electronically.

In FIG. 12, the deformable member is a doubly-clamped beam made from twolayers of SU-8 polymer and the transducer is a gold wire sandwichedbetween the polymer layers and patterned asymmetrically in thehorizontal plane using a c-shape. The transducer converts deformationsof the beam into electrical signals by the piezo-resistive effect,described in Roukes [P3]. Each force sensor is part of a Wheatstonebridge that includes two balance resistors and one reference beam inaddition to the force sensor.

The force sensors have been fabricated on a silicon-nitride coatedsilicon wafer and suspended over an opening etched in the wafer. Thisopening makes up part of the fluidic channel that surrounds the forcesensor. The rest of the fluidic channel is made from silicone rubber(Poly-DiMethyl-Siloxane or PDMS) based micro-fluidics that are not shownin this image.

The force sensors have been suspended from the wafer's surface byetching a hole through the wafer from the backside using a potassiumhydroxide etch to remove the silicon and a combination of a fluorinebased plasma etch and a hot, dilute hydrofluoric acid etch to remove thesilicon-nitride layer.

The hot, dilute hydrofluoric acid etch is important because itselectively and specifically etches the silicon-nitride without damagingthe polymer and metal that comprise the force sensor. The use of hot,dilute hydrofluoric acid to etch silicon-nitride is described in Knotter[P4] which focuses on selecting the etching of silicon-nitride oversilicon-dioxide in CMOS process. Accordingly, embodiments of theinvention provide for the use of hot, dilute hydrofluoric acid to etchsilicon-nitride for the purpose of suspending polymer structures withoutdamaging those polymer.

In the particular instance of a force sensor for measuring forces from acell, the hot, dilute hydrofluoric acid etch serves a second purpose:the hydrofluoric acid leaves the polymer surface hydrophobic and exposedgold regions hydrophilic. The hydrophobic and hydrophilic nature ofthese surfaces is critical for the surface chemistry techniquesdescribed below.

In the particular instance of a force sensor for measuring forces from acell with cell contact pads using a titanium adhesion layer, the hot,dilute hydrofluoric acid etch serves a third purpose: the hydrofluoricacid selectively removes the titanium adhesion layer to expose the goldpad without damaging the gold surface. Removal of the titanium adhesionlayer is critical to the surface chemistry techniques described below.

In addition to the above, the force sensors may be intended for usemeasuring forces exerted by individual adherent cells on theirsurroundings. This requires a cell contact area in close proximity tothe force sensors. The cell contact area is a relatively rigid areaadjacent to the force sensor upon which an adherent cell can makecontact and spread. In one or more embodiments, the cell contact area isdefined by a grid of metal (gold) squares. The gold squares can be usedto control where the cell attaches utilizing the surface chemistrytechniques. Similar gold squares have been patterned on each forcesensor in order to control the cell's attachment to the force sensorusing the same surface chemistry techniques.

Two types of surface chemistry may be provided in accordance withembodiments of the invention: The first type utilizes the hydrophobicnature of the polymer and the hydrophilic nature of the metal pads. Suchtechniques may be set forth in further detail in Tan [P5]. The secondtype utilizes thiol-gold chemistry to form Self-Assembled Monolayers(SAMs) on the metal pads. Such a type is described in Mrksich [P6].

The gold squares that make up the cell contact area on the relativelyrigid area and on the force sensors are initially deposited onsilicon-nitride and the polymer layers that make up the force sensor aredeposited on top of the gold squares. When the force sensors aresuspended using the hot, dilute hydrofluoric acid etch described above,the surface of the gold squares to be used for the surface chemistrydescribed above is exposed. The cleanliness and hydrophilic nature ofthe gold surface is critical for the surface chemistry. There are acouple of techniques that are critical for ensuring the cleanliness andhydrophilic nature of the gold surface.

An adhesion layer must be used to ensure the gold adheres to thesilicon-nitride during fabrication. Titanium is a commonly used adhesionpromoter for gold on silicon-nitride. However, after the force sensor issuspended the titanium adhesion layer must be removed in order to exposethe gold pad. The hot, dilute hydrofluoric acid etch selectively removesthe titanium without removing or damaging the gold.

An alternative to the titanium adhesion layer is an organic moleculecontaining a sulfur atom and a silane group, such asmercapto-tri-methoxy-silane (MPTS). Typically the MPTS is blanketdeposited over a silicon or silicon-derivative surface using a solventsolution (such a toluene). The gold layer is then blanket deposited overthe surface and patterning of the gold follows using lithography and agold etch process. These techniques are described in Ling [P7].

The above-described techniques may be insufficient for this process andapplication for two reasons: first, it may be necessary to patternsub-micron features in the gold pads which is hard to do using an etchmethod—liftoff is preferable. Second, there is a layer of gold alignmentmarks on the wafer that are needed for multiple layer steps, and theetch process would remove those alignment marks as well. To solve theseproblems, embodiments of the invention utilize a MPTS deposition processthat is compatible with metal deposition and patterning by lift-off. Thecritical step is to deposit the MPTS layer after developing the resistusing an aqueous solution with 0.1% acetic acid, which is described in adata sheet available from the Gelest Corporation (also see [P20-P22]).The aqueous solution does not damage the resist layer. This processworks well with electron beam resists such at PMMA and with i and g linephotoresists such at AZ5214e. Accordingly, embodiments of the inventiondeposit MPTS from an aqueous solution for this purpose.

Microfluidics

Microfluidic valve and pump systems such as those used in embodiments ofthe invention have been described before and have also been used toimplement a cell sorting system [P8]-[P18]. In this regard, references[P8]-[P18] describe a technology used to build multilayer silicone basedmicrofluidics with multiple flow channels, flow modalities andintegrated, and computer driven pneumatic controls.

However, none of the prior art systems have encapsulated a polymer NEMSforce sensor in microfluidics. In this regard, embodiments of theinvention provide for integrating microfluidics with NEMS force sensors.

The microfluidics serve a number of critical functions. Firstly,microfluidics enable delivery of individual cells to specific forcesensors. Secondly, microfluidics provide/enable precise control of thechemical environment around the cell/s under study. Precise control isnecessary for cell culture (keeping the cells alive). Additionally,precise control adds precision and control when perturbing the cellswith pharmacological agents. Third, significant “fan-out” wiring andelectronics are needed to extract signals from the force sensors out toa computer for readout and analysis. The microfluidics decouple the“fan-out” wiring from the fluid necessary for cells and biologicalstudies in general.

A minimal microfluidics system can be very simple, consisting of just afew parts and very basic function: In this regard, embodiments of theinvention provide for encapsulation of the force sensor to enclose,minimize and control the volume around the force sensor. Further,embodiments may merely comprise a single inlet and a single outlet.

Particular fabrication methods may include partial flow channels thatpass completely through the NEMS chip. For this reason, these NEMSdevices require encapsulation from two sides. One side of the NEMSdevice is encapsulated by a glass cover slip with a thin layer ofsilicone that acts as a glue and seal. The glass cover slip serves adual purpose: it encapsulates the device and enables high resolutionoptical microscopy that is compatible with use of the NEMS devices. Theother side of the NEMS device, which has the “fan-out” wiring and NEMSdevices is encapsulated with multilayer silicone based microfluidicswith multiple flow channels, flow modalities and integrated, computerdriven pneumatic controls.

FIG. 13 illustrates a polymer NEMs force sensor embedded inmicrofluidics in accordance with one or more embodiments of theinvention. As illustrated, the NEMS chip 1300 is encapsulated. Thetopside encapsulation 1302 includes multilayer silicone microfluidicswith multiple flow channels, flow modalities and integrated computerdriven pneumatics. The backside encapsulation 1304 includes a glasscover slip with a thin silicone layer for adhesion and sealing.

A list of the features of the multilayer silicone based microfluidicsused on the NEMS force sensor follows. The parts are labeled in FIG. 14,which illustrates a 2D diagram of the four layers that make up themicrofluidics in accordance with one or more embodiments of theinvention. Four layers of silicone are used to make the microfluidics.The uppermost layer, referred to as the “Incubator Layer” containsinter-digitated terminal lines which are filled with water andmaintained under pressure in order to saturate the silicone, which isgas permeable, with water vapor and thus prevent evaporation.

The Incubator Layer also contains a zig-zaging through line which can beused to flow gases through the silicone. Flowing mixtures of air andcarbon dioxide through the silicone is sometimes necessary for culturingcells within the microfluidics.

The second layer, referred to as the “Flow Layer” and referred to in thedrawings as flow lines and outlet lines, contains 12 inlets lines and 3outlet lines. There are two classes of inlet lines: low fluidicresistance lines with large diameter for flowing cells and the fastflowing of liquids and high fluidic resistance lines with small diameterfor slowly flowing liquids. Cells are very sensitive to fluidic shearforces so it is necessary to feed and perturb cells by slowly flowingliquids.

The flow lines are connected to the devices on the NEMS chip by way of“vias” that travel vertically through the third and fourth layers of thechip.

The third layer on the chip, the “Control Layer,” contains 34 pneumaticvalves which are used to control the flow in the flow layer. The valvesare used at flow inlets, outlets, to isolate lines that connect to theindividual force sensors, and in combinations to make a peristaltic pumpwhich can be used to precisely meter flow through the flow lines bothforward and backward.

There are also “vias” through the control layer that are vertical flowchannels that connect the flow layer to the fourth layer and the NEMSchip.

The fourth layer, the “base layer,” is in contact with the NEMS chip andcontains flow channels which run parallel to the channels in the NEMSchip and encapsulate the NEMS device while leaving it suspended.

The channels in the base layer contain vertical portions that connect tothe “vias” through the control layer and horizontal portions, which runalong the NEMS chip.

The base layer also includes a set of high resistance flow channels thatallow slow liquid flow to pass by the NEMS force sensor perpendicular tothe plane in which the sensor senses forces and out of the plane of thesensor. The purpose of this “out of plane” flow network is to enablefluid flow and reagent exchange for cells on the force sensor that doesnot mechanically perturb the NEMS force sensor.

Thus, as described above, a microfluidic system is used for variouspurposes. In addition to that stated above, the microfluidic system maybe used to position a cell where desired.

The target location for positioning can be any small object or surfaceupon which it is desirable to place a single cell. It can range in sizefrom as small as ˜100 square microns up to 10,000 square microns orlarger.

A microfluidic channel must pass over the target area. The microfluidicchannel confines the fluid flow, and thus cell location, in twodirections. The confined geometry of the microfluidic channel reducesthe Reynolds number for flow through the channel below 1. Thus the flowthrough the channel is laminar and the cell can be moved back andforth—reversibly—along a flow line without convective flow moving thecell in an uncontrolled manner.

In one or more embodiments, the valves may be positioned along the flowchannel so that the region around the target location can be sealed offfrom the rest of the microfluidic system once the cell has beenpositioned over the target area. Sealing a small region around thetarget area ensures that unintended flow with not move the cell awayfrom the target area while it is settling.

Further, as described above, a peristaltic pump, integrated into themicrofluidic channel, may be used to control the fluid flow and thus thecell's location. The pump can be operated forward or reverse to move thecell forwards and backwards along a flow line until it is located overthe target area. Clearly the cell must be on a flow line which passesover the target area, if the target area is centered in the microfluidicchannel this is not a difficult condition to meet. The minimumresolution of the cell positioning system is determined by thedisplacement volume of one of the valves in the peristaltic pump and thechannel cross section over the target area.

Once the cell has been positioned over the target location, valves areused to seal off the flow channel around the target area. Gravity willgently lower the cell onto the target location.

FIG. 15 is a schematic of a system utilized to position a cell inaccordance with one or more embodiments of the invention. In FIG. 15,the system is used to position NIH 3T3 fibroblast cells on plastic NEMsdevices with a target area of 1200 square microns. Similar to FIG. 14,there are 12 inlet lines on this system, four individually addressabletarget areas, one peristaltic pump and two outlet lines. One of theinlet lines is used to position a cell in the channel with the targetarea and the peristaltic pump is used to finely position the cell overthe device.

Force Measurement Results

As described above, one or more embodiments of the invention may providefor fabricating a device and high yields have been demonstrated (>60%).Successful micro-fluidic encapsulation is routine and consistentlyperformed at very high yields, (>90%). The force sensing capabilities ofthe devices have been tested and calibrated by perturbing the forcesensors with glass micro-needles mounted on piezo-electric actuators,data shown in FIG. 6A. The force sensors have been tested inmicro-fluidics be measuring their response to shear forces generated byfluid flow. The force sensors have been successfully used to measureforces exerted by individual adherent cells and to study the mechanicalresponse of those cells to cytoskeleton perturbing reagents such asCytochalasin D.

Data of force measurement from a single cell have shown a stable forcein growth media, collapse of that force when the cytoskeleton disruptingagent Cytochalasin D is introduced, and the recovery of the force whenthe Cytochalasin D is removed. Such measurements were performed with 200pN force resolution—an improvement of 25 fold over prior art—and 10 mstime resolution—and improvement of 300 fold over prior art.

FIG. 16 shows a SEM image of a dry force sensor prior to micro-fluidicencapsulation and a fluorescent image of a cell attached to the forcesensor on a micro-fluidics encapsulated device.

FIG. 17 shows force vs. time data from a single cell showing a stableforce in growth media, collapse of that force when the cytoskeletondisrupting agent Cytochalasin D is introduced, and the recovery of theforce when the Cytochalasin D is removed. These measurements wereperformed with 200 pN force resolution—an improvement of 25 fold overprior art—and 10 ms time resolution—and improvement of 300 fold overprior art.

Vacuum Insulating Polymer-Based Micro-Biocalorimeter Integrated withMicrofluidics

In addition to the above described force sensors, one or moreembodiments of the invention further provide for the use of amicro-biocalorimeter that is vacuum insulated, polymer based, andintegrated within microfluidics.

As described above, a calorimeter is a device for the measurement of theheat capacity of materials and the enthalpy change in chemicalreactions. Calorimetry is a technique widely used by the pharmaceuticalindustry, biologists and chemists to study the kinetics of biochemicalreactions and the reaction of living organisms and tissues to chemicals(e.g., drugs). In this regard, calorimeters have been used in diverseresearch areas in biology, such as studies of thermodynamic properties,structure and interactions of proteins because of universal nature ofheat generation in biochemical reaction and simple preparation ofsamples.

However, the use of calorimeters has been limited due to its largeconsumption of sample and long measurement time, typically >1 mL and 1hour. Microfabrication techniques have made it possible to build smallscale calorimeters to overcome these disadvantages. In thesecalorimeters, samples are prepared as either droplets on micro-sizesensing regions or flow through microfluidic channels. Microfabricatedthermometers are used to achieve very good temperature sensitivity.Measurement sensitivity of these calorimeters, however, are not as goodas large scale calorimeters, due to large device heat capacity andthermal conductance. There has been no serious attempt to increasesensitivity by minimizing the heat loss of the sample.

One or more embodiments of the invention provide a fabrication andoperation of a highly sensitive heat conduction calorimeter with vacuuminsulation, which can detect enthalpy change of reactions from ˜3.5nanoliter (nL) liquid sample. In this regard, a parylene polymer-basedmicro-biocalorimeter is integrated with microfluidics (also referred toas a “CIT calorimeter”) that is capable of performing batch, isothermaltitration and differential scanning calorimetric measurements on 50picoliter (pL) to 100 nanoliter (nL) volumes of chemical reagents andliving tissues. The calorimeter could also be configured as a detectorof chemicals and hazardous reagents. The major advantages of the CITcalorimeter over existing biocalorimeters are the following:

1. Small reagents volume: The volume of reagents used in the CITbiocalorimeter is significantly lower than that in conventionalcommercial biocalorimeters such as a MicroCal VP-ITC [CIT 1] which uses˜1 microliter (μL) of reagents. For many applications, this is veryuseful because reagents (such as a newly synthesized protein) could bevery expensive and scarce.

2. Liquid delivery by microfluidics: The use of a microfluidics systemwith on-chip pumping and valves enables automated delivery of liquidover other biocalorimeters that require manual injection. [CIT 1] [CIT2]. It also provides efficient delivery of small amounts of liquid atrelatively low cost compared to the traditional, “robotic-pipette”systems such as that used by the MiDiCal microplate system developed byVivactis. It furthermore allows easy interfacing with existing pipelines(e.g., a water distribution system) from which it could draw samples foranalysis. Devices including sensor and microfluidic controls can bepacked in very small volume and be easily developed as a hand-helddetector.

3. Simultaneous operation of multiple calorimeters: Because thecalorimeters are produced on inexpensive glass substrates by standardsemiconductor processing technologies, the user could obtain and operatemultiple (e.g., 100 to 1000) calorimeters simultaneously. This greatlyimproves the efficiency of calorimetric measurement. Moreover, this lowcost calorimeter is disposable, easy to use and saves cost on cleaning

4. Large bandwidth: The microcalorimeter promises a fast response at ˜1kHz. It could be used to trace the reaction of a cell to itssurroundings.

Overview—Design of the CIT calorimeter

The three major building blocks of the calorimeter are the thermometry,the microfluidics and the thermal isolated reagents compartment.

Microfluidics

The main microfluidic body is built with parylene. Microfluidic control,such as on chip pumps and valves, can be made in different ways. One wayis to build a PDMS microfluidic control and combine the control with aparylene channel. Another way is making on-chip electrostatic-actuatedpumps and valves on silicon or glass substrates by optical lithographyand parylene and metal deposition.

Thermometry

The thermometry is used to determine the temperature change due to thereactions of biochemical reagents. Thermopile thermometry of twothermoelectric components, such as gold and nickel, can be used which iseasy to fabricate and reliable. The thermopile thermometry with metallicthermoelements generally provides a responsivity of 200 to 500 μV/K.This is corresponded to a temperature sensitivity of ˜0.1 mK.

Thermal Isolated Reagents Compartment by Vacuum and Air Gap

The most critical part of a calorimeter to achieve pL-scale reagentvolumes is the design of the compartment for reagents. Because of thesmall volume of reagents and/or living tissues involved, the enthalpychange due to the biochemical reactions is very low. The typical powerof a biochemical reaction is 1 to 10 nW for 100 pL of reagents. Togenerate a resolvable temperature gradient from the power, the totalthermal conductance of the compartment to the environment must be verylow at ˜1 μW/K. Thus, the average conductivity of the constructingmaterial is 0.03 W/m K.

The most common forms of thermal isolation used for calorimeters arethermally resistive enclosures, [CIT 1] air cushions (generated bymembranes)[CIT 2][CIT 3] and insulating substrates. Such techniques arenot readily applicable to a 100 pL calorimeter. A resistive enclosurefor a 100 pL volume has to be made as small as the volume itself. Thesilicon nitride membranes used by the existing calorimeter arethemselves too conductive (thermal conductivity of silicon nitride is 30W/m K). Finally, everyday insulating materials such as foam are composedof air sacs that are as big as the calorimeter itself and could not beused as the substrate.

In one or more embodiments of the invention, a multi-layered parylenestructure is used for vacuum isolation, the suspended parylene structureis fabricated by standard semiconductor processing techniques andextends outward for ˜500 μm. FIG. 18 illustrates a cross section of sucha multilayer parylene calorimeter compartment in accordance with one ormore embodiments of the invention. As illustrated, the parylene 1802poles connect separate layers for mechanical support. The thermometer(not shown) is on the parylene membrane 1802 directly under thechemicals. The chemicals are brought into the chamber through amicrofluidics channel (not shown) and isolated from the channels byvalves (not shown).

An inexpensive mechanical pump is applied to create a vacuum 1804 of 1mbar. This is possible because of the low gas permeability of parylene1802. The 1 mbar vacuum, coupled with the small dimensions of the layer,has a thermal conductivity of 0.0005 W/m K. The resultant compartmenthas a thermal conductance of 0.1 μW/K from the vacuum 1804 (residualair) and 0.4 μW/K from the parylene membrane 1802. Thus, the totalthermal conductance of the compartment is 0.5 μW/K.

One can emphasize the unique nature of parylene for construction of thecompartment because of its low thermal conductivity, gas permeabilityand available valve structures. Many polymers, such as SU-8, could formsimilar structures. However, since they could not form valves, thereagent compartment is not cut off from the fluidic channels, whichresults in large thermal leaks. On the other hand, common microfluidicsmaterials, such as PDMS, are highly permeable to gas and very soft, andso could not support a vacuum.

In addition, a prototype of a parylene microcalorimeter is illustratedin FIG. 19. FIG. 19 shows the reaction chamber on a suspended parylenemembrane, the microfluidics channels for fluid delivery, and thethermopile for sensing heat release. The additional layers for buildingthe vacuum pocket are not shown. As illustrated, a simple structurehaving two input channels and a single output channel is illustrated.The two inputs are combined in the reaction chamber and heated. Theelectrical contact is used to measure and output the enthalpy change.

Detailed Description—CIT Calorimeter

The above description provides an overview of a parylenemicrocalorimeter in accordance with embodiments of the invention. Adetailed description of such a calorimeter follows.

The calorimeter consists of thin film thermopile,parylene-polydimethylsiloxane (PDMS) hybrid microfluidic system andvacuum insulation structure. FIG. 20 illustrates a schematics of acalorimeter in accordance with one or more embodiments of the invention.FIG. 21 illustrates a whole chip embodying the calorimeter in accordancewith one or more embodiments of the invention. FIG. 22 illustrates adetailed view of a calorimeter chamber and electric sensor built on aparylene membrane in accordance with one or more embodiments of theinvention. The following description refers to aspects of FIGS. 20-22.

Both sides of the parylene membrane 2002 are under vacuum duringmeasurement. Thermopile 2004 is buried between two parylene layers 2002and protected from the sample, which is placed into the chamber 2006.Au/Ni metallic thermopile 2004 is chosen as a thermometer because offabrication convenience and low electric noise. 5 thermocouple junctionsare connected in parallel to give ˜110 μV/K temperature coefficient (ε).

FIG. 21 illustrates an image of a calorimeter implementation inaccordance with one or more embodiments of the invention. Asillustrated, the fluid is placed into the channels via various fluidicdistribution members 2102. After sensing the enthalpy change, thecalorimeter is used to produce an electrical output on contact pads2104. The glass top and vacuum chuck serves to seal the chip and createa vacuum chamber as described herein. Similarly, FIG. 22 illustrates theheater 2202, electrical contacts/thermopile 2204, reaction/calorimeterchamber 2206, pumping hole 2208, vacuum chamber 2210, and parylenemembrane 2212 used to measure the enthalpy change.

Referring again to FIG. 20, parylene 2002 is used to build themicrofluidic channel and calorimeter chamber 2006, because parylene 2002has many advantages in property such as chemical inertness,biocompatibility. However, parylene is not compliant as PDMS and theremay not be an easy mechanism to incorporate valves or pump. Thus, PDMSmicrofluidic valves and pumps may be combined with parylene microfluidicchannels for better manipulation of samples. To secure the PDMSmicrofluidic structure 2008, the parylene channel 2002 is planarizedwith thick SU-8 2010. PDMS fluidic channels 2008 are aligned on parylenechannels 2010 opening and further cured to be bonded on SU-8. FIG. 23 isan image illustrating an alignment of the fluidic channels on parylenechannels (i.e., a parylene-su8-pdms junction) in accordance with one ormore embodiments of the invention.

PDMS peristaltic pumps are used to move liquid through the channel. Fora batch mode measurement, a reactant is used to fill up to half of thereaction chamber 2006, and then second reactant is delivered to thereaction chamber 2006 (e.g., via the microfluidic channel created viaPDMS 2008, SU-8 2010 and parylene 2002. The second reactant is mergedwith the first reactant. FIG. 24 illustrates three images of merging tworeactants in accordance with one or more embodiments of the invention.

Reaction from reactants in the channel may be ignored because its volumeis very small compared to total chamber volume. Reactants far fromchambers are considered as not participating in reaction due to longdiffusion time.

For a microscale calorimeter, it's very challenging to keep the heatcapacity of addenda small while reducing the sample volume. Forinstance, when the sample is surrounded by bulky microfluidic material,much of sensitivity is lost due to huge heat loss to chamber wall.Parylene microfluidic channels can have only ˜1 μm thick wall, so it canreduce heat loss significantly and even replace SiN membrane, which isused for the most of microscale calorimeter even though it is quiteconductive. Even more reduction of the heat loss can be accomplished byaccommodating on-chip vacuum capability. Parylene thin film 2002 cangive very low gas permeability and mechanical strength, which enablesthe application of vacuum insulation on the device. With nanoliter scalesample volume, the surface to volume ratio of the sample becomessignificantly large, resulting in significant heat loss from thesurface. This implies that even heat loss through air to the environmentcan significantly affect the sensitivity.

FIG. 25 shows the effect of a vacuum on device thermal conductance (G).As illustrated, the amount of conductance improves significantly as thepressure P vacuum is applied. The on-chip vacuum chamber has tworegions. The region above the parylene membrane 2002 is defined by theSU-8 2010 on the side and the glass ceiling 2012. The region 2014 belowthe membrane 2002, formed by KOH etching for a SiN membrane, is sealedby an o-ring and a vacuum chuck. A 2 μm thick parylene channel providesenough mechanical strength and isolation of gas or liquid inside thechamber 2006 from the vacuum. One can observe chamber volume change dueto parylene stretching under pressure difference between the inside andthe outside of the chamber 2006. The volume after applying a vacuum wasmeasured to be ˜3.5 nl. The small membrane left upper corner was built,and removed later, to pump the upper region.

To calibrate the thermometer signal, thermoelectric voltage response wasmeasured over electric power applied on the gold heater. The heat powersensitivity (Sp), which is defined as voltage output over applied power,was 5V/W. Since S_(P)=ε/G, both increase in &, for example use highSeebeck coefficient material and decrease in G can give bettersensitivity. However, materials with a high Seebeck coefficient, such asdoped Si, usually has high electric resistivity and give large electricnoise on thermoelectric voltage measurement. The resistance of Ni/Authermopile was ˜1.1 kΩ and the noise at 1 Hz was ˜10 nVrms/√Hz, whichcorresponds to equivalent power noise of ˜2 nW/√Hz.

Thermal conductance was 22 μW/K. According to the finite elementsimulation, it can be as small as 5 μW/K if the air conductance wasminimized. This result implies the vacuum insulation did not reach itsbest with only one layer of vacuum sac. Multiple layers of vacuum sac orhigher vacuum is expected to improve the overall sensitivity by loweringthe thermal conductance.

In view of the above, embodiments of the invention provide a highlysensitive microfluidic embedded calorimeter. Integration of amicrofabricated thermal sensing element, microfluidic system and on-chipvacuum structure enable the ability to measure the nanocalorie scaleheat of reactions from 3.5 nl samples.

Device sensitivity on thermometer side has not pushed to its limit.Thermopile material with high Seebeck coefficient and multiplication ofsignal by increasing number of thermocouple junction may provideincreased temperature sensitivity. In addition, careful balancing ofthermal conductance of each element may provide a further reduction inthermal conductance.

Although single device operation are described herein, multiple devicesmay also used to increase throughput or to be deployed as detectorarray. All of the fabrication steps are compatible with mass production.The device concept can also be applicable to different type ofcalorimeters such as isothermal titration calorimeter (ITC),differential scanning calorimeter (DSC) and flow calorimeter, withsimple geometry change.

Fabrication and Use—CIT calorimeter

To make a suspended parylene membrane, one first builds a 1.5 mm squareSiN membrane with a double side polished SiN wafer. This SiN membrane isremoved by Reactive Ion Etch (RIE) at the end of fabrication steps. 1 μmthick parylene is deposited on the SiN with PDS 2010 LABCOTER® 2,parylene coater. As a thermometer and a resistive heater, 90 nm thick Niand 80 nm thick Au are e-beam evaporated on parylene. 4 nm thick Ti isevaporated as adhesion layer for both Ni and Au. They are patterned byphotolithography and chemical wet etch. A 1 μm thick 2^(nd) parylenelayer is coated as a protective layer. The parylene microfluidic channelcan be built in conventional method. A 15 μm thick photoresist is spunand patterned into the microfluidic chamber and the channel structure. A3^(rd) parylene layer, 2 μm thick, is deposited on the photoresist tobuild the parylene microfluidic channel. A ˜80 μm thick SU-8 structureis built on top of the parylene microfluidic structure to planarize thesurface and to construct the vacuum chamber.

Several etching steps can be conducted by RIE. First, the parylenemicrofluidic channel opening area was etched (O2 plasma 150 mT, 140 W).The photoresist filling inside the channel is removed using propyleneglycol methyl ether acetate (PGMEA). After the microfluidic channel iscleared, parylene covering the electric contact area is etched (O2plasma 150 mT, 140 W). Finally, the parylene membrane is suspended aloneby etching away SiN underneath (CF4 plasma 120 mT, 140 W). The vacuumchamber region is sealed with a glass slide using UV curable glue.

Electrical Measurements may be obtained using the device describedherein. Thermal conductance and the device time constant is measured byapplying step function heating voltage to the heater. Calorimetertemperature response to applied power can be represented as

${\Delta\; T} = {\frac{P}{G}{\left( {1 - {\mathbb{e}}^{- \frac{t}{\tau}}} \right).}}$For heat of reaction measurement, thermoelectric voltage can be directlyrecorded by oscilloscope. FEMTO low noise preamplifier with 2.3 nV/√Hzinput noise can be used to amplify the signal.Logical Flow

FIG. 26 illustrates the logical flow for creating and utilizing amicrofluidic embedded NEMS force sensor in accordance with one or moreembodiments of the invention. At step 2602 the force sensor is created.Such a force sensor is comprises a deformable member that is integratedwith a strain sensor. The strain sensor coverts a deformation of thedeformable member into an electrical signal.

The deformable member may be a doubly clamped beam and the strain sensormay be a piezo resistive strain sensor that is patterned asymmetricallythrough the doubly clamped beam so as to couple to regions of maximumtensile or compressive strain. The piezo resistive strain sensor may bea c-shape that is patterned in the horizontal plane of the doublyclamped beam and is used to measure in-place forces. Alternatively, thestrain sensor may be patterned using a straight line pattern to measureout-of-plane forces.

The force sensor may be fabricated from a polymer. In this regard, thestrain sensor may be sandwiched between two layers of polymer toelectrically isolate the strain sensor from the fluid in the fluidicenvironment.

In addition to the above, the force sensor may consist of the deformablemember and a transducer used for reading out the electrical signal. Insuch an embodiment, the deformable member may be a doubly-clamped beammade from two polymer layers and the transducer may be a gold wiresandwiched between the two polymer layers. Further, the force sensor maybe fabricated on a silicon-nitride coated silicon wafer and suspendedover an opening etched in the wafer. Such an opening comprises part ofthe microfluidic channel that surrounds the force sensor. Also, theforce sensor is suspended from the wafer's surface over a hole etchedthrough the wafer's backside. A contact area on the force sensor mayalso be defined by a metal region or a grid of metal regions thatcontrol where a biological sample exerts a force on the force sensor.The metal layer may adhere to the silicon substrate using an organicadhesion promoter and is patterned using metal liftoff.

In terms of fabricating the force sensor, multiple steps may beinvolved. A first polymer layer may be deposited onto a silicon-nitridelayer coating a silicon wafer. A metal wire may then be deposited (onthe first polymer layer) that provides a piezo-resistive element of astrain sensor. A second polymer layer is deposited on the metal wire andthe first polymer layer. A hole can then be etched through the wafer'sbackside. The force sensor can then be defined by creating a polymerstructure, from the first polymer layer and second polymer layer, thatencapsulates the metal wire, and that is suspended over the hole, byremoving the silicon-nitride layer from a portion of the wafer, withoutdamaging the first polymer layer and the second polymer layer. Theopening may define part of a fluidic channel that surrounds the forcesensor. Further, the hole may be etched through the wafer's backsideusing potassium hydroxide. The silicon-nitride layer can be removed froma portion of the wafer using a combination of a flourine based plasmaand a hot dilute hydrofluoric acid.

A further part of the fabrication process may include depositing a metallayer for controlling cell adhesion to the force sensor. Such a metallayer may consist of a grid of metal squares that control where abiological sample exerts a force on the force sensor.

At step 2604, the force sensor is encapsulated in a microfluidicchannel. The channel serves to control a fluidic environment around theforce sensor and improves an electrical read out (or enables a preciseelectrical readout) of the electrical signal from the force sensor.

At step 2606, the force sensor is used to measure the force exerted(e.g., by a biological sample/single cell).

FIG. 27 illustrates a method for utilizing a microfluidic embeddedvacuum insulated biocalorimeter in accordance with one or moreembodiments of the invention.

At step 2702, a calorimeter chamber is created using a parylenemembrane. Both sides of the calorimeter chamber are under vacuum duringmeasurement of a sample. Thus, the calorimeter chamber may consist oftwo regions. A first region adjacent the parylene member can be definedby SU-8 on a first side and glass on a second side. The second region isadjacent the parylene member and can be formed by potassium hydroxide(KOH) etching for a SiN (Silicon nitride) membrane that is sealed.

At step 2704, a microfluidic channel is created. Such a channel is usedto deliver a sample to the calorimeter chamber. Further, the channel isbuilt from the parylene membrane.

At step 2704, a thermopile (e.g., a nickel/gold), used as a thermometer,is encapsulated/located between two layers of the parylene membrane andis protected from the sample. Further, multiple layers of vacuum can beutilized to provide further insulation of the sample.

At step 2708, the biocalorimeter is used to measure the enthalpy changeof biological samples in the chamber. A PDMS(parylene-polydimethylsiloxane) peristaltic pump can be used to move thesample in liquid along the microfluidic channel to obtain themeasurement.

CONCLUSION

The foregoing description of the preferred embodiment of the inventionhas been presented for the purposes of illustration and description. Itis not intended to be exhaustive or to limit the invention to theprecise form disclosed. Many modifications and variations are possiblein light of the above teaching. It is intended that the scope of theinvention be limited not by this detailed description, but rather by theclaims appended hereto.

REFERENCES

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What is claimed is:
 1. A microfluidic embedded vacuum insulatedbiocalorimeter comprising: a calorimeter chamber comprising a parylenemembrane, wherein both sides of the calorimeter chamber are under vacuumduring measurement of a sample; a microfluidic channel used to deliver asample to the calorimeter chamber, wherein the microfluidic channel isbuilt from the parylene membrane; and a thermopile, used as athermometer, located between two layers of the parylene membrane andprotected from the sample.
 2. The biocalorimeter of claim 1 wherein aPDMS (polydimethylsiloxane) peristaltic pump is used to move the samplein liquid along the microfluidic channel.
 3. The biocalorimeter of claim1, wherein the calorimeter chamber comprises: a first region adjacentthe parylene member defined by SU-8 on a first side and glass on asecond side; and a second region adjacent the parylene member formed bypotassium hydroxide (KOH) etching for a SiN (Silicon nitride) membranethat is sealed.
 4. The biocalorimeter of claim 1, wherein multiplelayers of vacuum provide insulation of the sample.
 5. The biocalorimeterof claim 1, wherein the thermopile comprises an AuNi alloy (GoldNickel).
 6. A method for measuring an enthalpy change of a sample in amicrofluidic embedded vacuum insulated biocalorimeter, comprising:creating a calorimeter chamber comprising a parylene membrane, whereinboth sides of the calorimeter chamber are under vacuum duringmeasurement of the sample; creating a microfluidic channel used todeliver a sample to the calorimeter chamber, wherein the microfluidicchannel is built from the parylene membrane; and encapsulating athermopile, used as a thermometer, between two layers of the parylenemembrane and protected from the sample; and measuring the enthalpychange of the sample in the calorimeter chamber.
 7. The method of claim6 further comprising moving the sample in liquid along the microfluidicchannel utilizing a PDMS (polydimethylsiloxane) peristaltic pump.
 8. Themethod of claim 6, wherein the calorimeter chamber is created by:defining a first region adjacent the parylene member by SU-8 on a firstside and glass on a second side; and forming a second region adjacentthe parylene member by potassium hydroxide (KOH) etching for a SiN(Silicon nitride) membrane that is sealed.
 9. The method of claim 6,further comprising insulating the sample using multiple layers ofvacuum.
 10. The method of claim 6, wherein the thermopile comprises anAuNi alloy (Gold Nickel).